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Novel bluetongue virus serotype from Kuwait.

Bluetongue virus (BTV) infects ruminants, camelids, and occasionally large carnivores. Clinical signs of bluetongue disease (BT) are usually more severe in sheep or white-tailed deer, particularly in populations previously unexposed to the virus; cattle and goats are often asymptomatic (1). Initial diagnosis of BT based on clinical signs can be confirmed by virus isolation and characterization or identification of viral RNA by reverse transcription PCR.

BTV particles contain 3 concentric protein layers surrounding 10 linear double-stranded RNA genome segments, identified as segment-1 to segment-10 (Seg-1 to Seg-10) in order of decreasing size (from 3,954 bp to 822 bp) (2). Twenty-five BTV serotypes have been identified on the basis of the specificity of reactions with neutralizing antibodies generated by their mammalian hosts (3). Consequently, BTV outer capsid proteins, particularly viral protein (VP) 2 (encoded by Seg-2), show sequence variations that determine virus serotype (4). Other BTV proteins, including subcore shell protein VP3(T2) encoded by Seg-3, are more highly conserved (2). Phylogenetic comparisons of Seg-3 sequences have been used to identify different BTV topotypes and distinguish different Orbivirus species (4).

BTV has been reported in several Middle Eastern countries (Egypt, Jordan, Syria, Turkey, Cyprus, and Iraq) since 1951 (5). In 2008, Egypt reported the absence of BT, and Egypt is the only country in the region to have prohibited BTV vaccination (5). Iran reported outbreaks of BT in 2008, and Saudi Arabia reported infection without clinical signs, although the serotype(s) were not identified (5). Multiple serotypes were detected in Israel during 2008 (5) and Oman in 2009 (S. Maan et al., unpub. data). We report characterization of a novel BTV serotype identified in Kuwait in 2010.

The Study

During February 2010, sheep and goats in the Abdali region of Kuwait, close to the Iraq border, showed the following clinical signs consistent with BT: lameness, coughing, mouth lesions, stillbirth, congenital abnormalities, pneumonia, enteritis, and hepatitis. Forty-six of 48 serum samples were positive for BTV-specific antibodies by competitive ELISA (Investcare-Vet, London, UK) at the Veterinary Diagnostic Laboratory and Animal Research Center in Kuwait, or by double antigenrecognition ELISA (ID Vet, Montpellier, France) at the Institute for Animal Health in the United Kingdom.

Twenty-six EDTA-treated blood samples, 4 spleens, and 1 liver sent for analysis for BTV to the World Organisation for Animal Health reference laboratory at the Institute for Animal Health (Woking, UK) all gave negative results by real-time reverse transcription-PCR (rRT-PCR) targeting either BTV Seg-1 (6) or Seg-1 and Seg-5 (7). However, 2 blood samples (from animals 364 and 374) were positive in assays selective for Seg-10 (8), with cycle threshold (Ct) values of 35 and 28, respectively. Previous attempts to isolate BTV from blood samples with Ct values >32 were usually unsuccessful, and no further work was done with animal 364. Washed blood from animal 374 (reference collection sample KUW2010/01) (9) was injected into embryonated chicken eggs. Although no hemorrhages were detected, the virus was passaged twice in BHK-21 cells (isolate KUW2010/02), producing atypical cytopathic effects.

KUW2010/02 RNA analyzed by agarose gel electrophoresis generated a genome segment migration pattern (electropherotype) typical of BTV (Figure 1). Although KUW2010/02 was negative by BTV-specific rRT-PCR selective for Seg-1 (6), it had Ct values of 16.8 in Seg-10-specific assays (8). Identification of KUW2010/02 as BTV was confirmed by indirect antigen-sandwich ELISA selective for core protein VP7(T13) (10) with optical density at 490 nm values >0.15 (equivalent BTV titer of 6.75 [log.sub.10] 50% tissue culture infective dose/mL).

RNA from KUW2010/01 and KUW2010/02, extracted by using TRIzol (Invitrogen, Carlsbad, CA, USA) (11), gave uniformly negative results by type-specific rRT-PCRs targeting Seg-2 of BTV serotypes 1-25 (kits supplied by Laboratoire Service International, Lissieu, France). However, full-length cDNA copies of Seg-2 (2,929 bp) and Seg-3 (2,773 bp) from KUW2010/02 were synthesized and then sequenced as described (11), showing conserved terminal regions typical of BTV (5'-GUUAAA.... ACUUAC-3') (2). BLAST (www. ncbi.nlm.nih.gov/BLAST) analysis of KUW2010/02 Seg-2 and Seg-3 sequences (GenBank accession nos. HM590642 and HM590643) showed highest identity with equivalent genome segments of other BTVs, although for Seg-2 the search algorithm was changed from megablast (highly similar sequences) to blastn (somewhat similar sequences).

[FIGURE 1 OMITTED]

Phylogenetic analysis of KUW2010/02 Seg-3/ VP3(T2), conducted by using neighbor-joining methods and p-distance matrices (12), showed nucleotide/amino acid identity levels of 73.7%/87.6% to 76.6% /88.9% with other BTVs. Seg-3 of none of the previously characterized BTVs showed close relationships to KUW2010/02; BTV-1/ GRE2001/05 and BTV-25/TOV were most closely related (GenBank accession nos. DQ186822 and GQ982523, respectively), which indicates that KUW2010/02 represents a distinct geographic cluster or topotype (4).

Seg-2/VP2 of KUW2010/02 showed nucleotide/amino acid identity levels of 42.8%/28.3% to 63.9%/61.5% with previously recognized BTV serotypes and was most closely related to BTV-25 (nucleotype K, Figure 2). Reference strains of BTV-10 and BTV-17 from the United States (nucleotype A) were the next most closely related, with 61.8%/58.1% and 62%/57.7% nt/aa identity, respectively. This places KUW2010/02 as a distinct virus type within a novel 12th Seg-2 nucleotype L (4; Figure 2). Clustal-X (www.clustal.org) alignments and neighbor-joining trees also confirmed the identity of KUW2010/02 as a BTV. Virus neutralization tests of KUW2010/02 (13) that used reference guinea pig immune serum against BTV types 1-24 and antiserum from goats previously infected with BTV-25 showed no reduction in KUW2010/02 infectivity (data not shown), demonstrating that it does not belong to BTV serotypes 1-25.

Conclusions

Most serum samples tested from sheep and goats in Kuwait showing clinical signs of disease were seropositive for BTV-specific antibodies. However, BTV RNA was detected in only 2 sheep serum samples (animals 364 and 374), suggesting that the clinical signs were not caused by ongoing BTV infection. All samples were also tested for peste des petits ruminants virus by rRT-PCR (14), but results were uniformly negative.

BTV RNA was detected by using a BTV Seg-10-specific rRT-PCR (8) previously used to detect BTV-25 in Switzerland (15). However, BTV Seg-1- or Seg-1- and Seg-5-specific assays (6,7) failed to detect KUW2010/02, identifying it is an unusual or atypical BTV strain. Alignment of the Seg-1-specific and Seg-5-specific primers and probes with KUW2010/02 sequences identified numerous mismatches that would prevent detection of the viral RNA (data not shown). However, the probe and primers designed by Orru et al. (8) showed a perfect match with Seg-10 of KUW2010/02, demonstrating the need for appropriate rRT-PCR protocols to detect this virus. Agarose gel electrophoresis analysis of KUW2010/02 genome segments generated a migration pattern typical of BTV (Figure 1). Levels of nucleotide/amino acid identity of Seg-3 (up to 76.6%/89%) of KUW2010/02 with other BTV isolates also identified it as BTV.

At peak viremia, a previously unexposed sheep infected with a virulent BTV strain could be expected to show Ct values -20. The Ct of 28 obtained with blood of animal 374 (KUW2010/01) indicates a low viremia, suggesting that the severe clinical signs observed were not caused by BTV. Experimental infection of previously unexposed sheep with KUW2010/02 also caused only mild clinical signs (data not shown).

Different isolates of a single BTV serotype show >68.4%/72.6% nt/aa identity in Seg-2/VP2, with 40.5%/ 22.1% to 71.5%/77.8% identity between different serotypes (4). KUW2010/02 showed only 42.8%/28.3% to 63.9%/61.5% identity in Seg-2/VP2 with recognized BTV serotypes, consistent with membership of a novel 26th BTV type and Seg-2 nucleotype (L) (4). These conclusions were supported by virus neutralization test results. The sequence data presented here will help support development of new diagnostic tools (RT-PCR-based typing assays) to determine the incidence and distribution of this novel serotype, as well as natural reservoir(s) and insect vectors.

[FIGURE 2 OMITTED]

DOI: 10.3201/eid1705.101742

Acknowledgments

We thank international colleagues who provided virus isolates for analyses and comparisons.

This study received funding support from the Department for Environment, Food and Rural Affairs, UK; the European Commission (OrbiVac grant no. 245266; WildTech grant no. 222633-2); Emerging and Major Infectious Diseases of Livestock grant OrbiNet K1303206; World Organisation for Animal Health; and Biotechnology and Biological Sciences Research Council, UK.

Dr Sushila Maan is a veterinarian and senior postdoctoral researcher in the Vector-borne Viral Diseases Programme at the Institute for Animal Health, Pirbright, UK. Her current research interests include characterization of BTV and the molecular epidemiology and diagnosis of BTV infection and other related orbiviruses.

References

(1.) Darpel KE, Batten CA, Veronesi E, Shaw AE, Anthony S, Bachanek-Bankowska K, et al. Clinical signs and pathology shown by British sheep and cattle infected with bluetongue virus serotype 8 derived from the 2006 outbreak in northern Europe. Vet Rec. 2007;161:25361. doi:10.1136/vr.161.8.253

(2.) Attoui H, Maan S, Anthony SJ, Mertens PPC. Bluetongue virus, other orbiviruses and other reoviruses: their relationships and taxonomy. In: Mellor PS, Baylis M, Mertens PPC, editors. Bluetongue monograph. 1st ed. London: Elsevier/Academic Press; 2009. p. 23-52.

(3.) Mertens PPC, Pedley S, Cowley J, Burroughs JN, Corteyn AH, Jeggo MH, et al. Analysis of the roles of bluetongue virus outer capsid proteins VP2 and VP5 in determination of virus serotype. Virology. 1989;170:561-5. doi:10.1016/0042-6822(89)90447-9

(4.) Maan S, Maan NS, van Rijn PA, van Gennip RGP, Sanders A, Wright IM, et al. Full genome characterisation of bluetongue virus serotype 6 from the Netherlands 2008 and comparison to other field and vaccine strains. PLoS ONE. 2010;5:e10323 doi:10.1371/ journal.pone.0010323.

(5.) World Organisation for Animal Health. OIE 2009: final report of the 10th conference of the OIE Regional Commission for the Middle East Doha (Qatar), 26-29 October 2009 [cited 2011 Mar 11]. http://www.rr-middleeast.oie.int/download/ pdf/Final%20Report_Doha_%20Qatar.pdf

(6.) Shaw AE, Monaghan P, Alpar HO, Anthony S, Darpel KE, Batten CA, et al. Development and validation of a real-time RT-PCR assay to detect genome bluetongue virus segment 1. J Virol Methods. 2007;145:115-26. doi:10.1016/j.jviromet.2007.05.014

(7.) Toussaint JF, Sailleau C, Breard E, Zientara S, De Clercq K. Bluetongue virus detection by two real-time RT-qPCRs targeting two different genomic segments. J Virol Methods. 2007;140:115-23. doi:10.1016/j.jviromet.2006.11.007

(8.) Orru G, Ferrando ML, Meloni M, Liciardi M, Savini G, De Santis P. Rapid detection and quantitation of bluetongue virus (BTV) using a molecular beacon fluorescent probe assay. J Virol Methods. 2006;137:34-42 doi:10.1016/j.jviromet.2006.05.028.

(9.) Mertens PPC, Attoui H. Isolates of bluetongue virus (BTV) in the dsRNA virus collection at IAH Pirbright [updated 2010 Jun 23; cited 2010 Jul 25]. http://www.reoviridae.org/dsRNA_virus_proteins/ ReoID/BTV-isolates.htm.

(10.) Thevasagayam JA, Wellby MP, Mertens PP, Burroughs JN, Anderson J. Detection and differentiation of epizootic haemorrhagic disease of deer and bluetongue viruses by serogroup-specific sandwich ELISA. J Virol Methods.1996;56:49-57.

(11.) Maan S, Rao S, Maan NS, Anthony SJ, Attoui H, Samuel AR, et al. Rapid cDNA synthesis and sequencing techniques for the genetic study of bluetongue and other dsRNA viruses. J Virol Methods. 2007a;143:132-9. doi:10.1016/j.jviromet.2007.02.016

(12.) Tamura K, Dudley J, Nei M, Kumar S. MEGA4: Molecular Evolutionary Genetics Analysis (MEGA) software version 4.0. Mol Biol Evol. 2007;24:1596-9. doi:10.1093/molbev/msm092

(13.) Grist NR, Ross CA, Bell EJ. Neutralization tests. In: Grist NR, Ross CA, Bell EJ, editors. Diagnostic methods in clinical virology, 2nd ed. London: Blackwell Scientific Publications; 1974. p. 64-79.

(14.) Batten CA, Banyard A, King D, Henstock M, Edwards L, Sanders A, et al. A real-time PCR assay for the specific detection of peste des petits ruminants virus. J Virol Methods. 2011;171:401-4.

(15.) Hofmann MA, Renzullo S, Mader M, Chaignat V, Worwa G, Thuer B. Genetic characterization of Toggenburg orbivirus, a new bluetongue virus from goats Switzerland. Emerg Infect Dis. 2008;14:1855-61. doi:10.3201/eid1412.080818

Author affiliations: Institute for Animal Health, Woking, UK (S. Maan, N.S. Maan, K. Nomikou, C. Batten, F. Antony, M.N. Belaganahalli, C.A.L. Oura, P.P.C. Mertens); Public Authority of Agriculture Affairs and Fish Resources, Kuwait City, Kuwait (A.M. Samy, A.A. Reda, S.A. Al-Rashid, M. El Batel); and Cairo University, Cairo, Egypt (A.M. Samy)

Address for correspondence: Peter P.C. Mertens, Vector-borne Viral Diseases Programme, Institute for Animal Health, Ash Rd, Pirbright, Woking, Surrey, GU24 0NF, UK; email: peter.mertens@bbsrc.ac.uk
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Article Details
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Title Annotation:DISPATCHES
Author:Maan, Sushila; Maan, Narender S.; Nomikou, Kyriaki; Batten, Carrie; Antony, Frank; Belaganahalli, Ma
Publication:Emerging Infectious Diseases
Article Type:Report
Geographic Code:7KUWA
Date:May 1, 2011
Words:2132
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